Cage-Like Bifunctional Chelators, Copper-64 Radiopharmaceuticals and PET Imaging Using the Same

ABSTRACT

Disclosed is a class of versatile Sarcophagine based bifunctional chelators (BFCs) containing a hexa-aza cage for labeling with metals having either imaging, therapeutic or contrast applications radiolabeling and one or more linkers (A) and (B). The compounds have the general formula 
     
       
         
         
             
             
         
       
         
         
           
             where A is a functional group selected from group consisting of an amine, a carboxylic acid, an ester, a carbonyl, a thiol, an azide and an alkene, and B is a functional group selected from the group consisting of hydrogen, an amine, a carboxylic acid, and ester, a carbonyl, a thiol, an azide and an alkene. Also disclosed are conjugate of the BFC and a targeting moiety, which may be a peptide or antibody. Also disclosed are metal complexes of the BFC/targeting moiety conjugates that are useful as radiopharmaceuticals, imaging agents or contrast agents.

CROSS-REFERENCE TO RELATED APPLICATIONS

The present application is a divisional of application Ser. No. 12/695,125 filed Jan. 27, 2010, which claims the benefit of U.S. Provisional Application No. 61/147,709, filed Jan. 27, 2009, the entire contents of all of which are incorporated herein by reference.

STATEMENT REGARDING FEDERALLY SPONSORED RESEARCH AND DEVELOPMENT

This work was supported by research grant from the Department of Energy. The government has certain rights in the invention.

BACKGROUND OF THE INVENTION

Molecular imaging is an emerging technology that allows for visualization of interactions between molecular probes and biological targets. Positron emission tomography (PET), micro-PET and PET/CT, are state-of-the-art nuclear medicine imaging modalities, which use nano- to picomolar concentrations of the corresponding probes (radiotracers) to achieve images of biological processes within the living system. Selection of the proper radionuclide and synthetic approach for radiotracer design are critical. Positron-emitting isotopes frequently used include ¹¹C and ¹⁸F. One non-traditional PET radionuclide, ⁶⁴Cu, shows promise as both a suitable PET imaging and therapeutic radionuclide due to its nuclear characteristics (T_(1/2)=12.7 h, β⁺+: 17.4%, E_(β+max)=656 keV; β⁻: 39%, E_(β−max)=573 keV), and the availability of its large-scale production with high specific activity.

Stable attachment of radioactive ⁶⁴Cu²⁺ to targeted imaging probes requires the use of a bifunctional chelator (BFC), which is used to connect a radionuclide and bioactive molecule to form the ⁶⁴Cu-radiopharmaceutical. Extensive efforts have been devoted to the development of BFCs for ⁶⁴Cu labeling. Three of the most common chelators studied have been the macrocyclic ligands DOTA (1,4,7,10-tetraazacyclododecane-N,N′,N″,N″′-tetraacetic acid), TETA (1,4,8,11-tetraazacyclotetradecane-N,N′,N″,N″′-tetraacetic acid), and cross-bridged tetraamine ligands. (Refs. 1-3) However, dissociation of ⁶⁴Cu from the BFC in vivo and harsh labeling conditions (e.g., incubation at 75° C. under basic conditions) impair the use of these chelators in preparing biomolecule-based ⁶⁴Cu-radiopharmaceuticals. (Ref. 4) The BFC DOTA has been used for ⁶⁴Cu²⁺ labeling. (Refs. 3, 5, 6) However, the limited stability of the copper chelate in vivo has hindered its application. (Ref. 37)

The integrin α_(v)β₃ receptor has been the attractive target of intensive research given its major role in several distinct processes, such as tumor angiogenesis and metastasis, and osteoclast mediated bone resorption. (Refs. 7, 8) The molecular imaging of integrin α_(v)β₃ expression will allow the detection of cancer and other angiogenesis related diseases, patient stratification, and treatment monitoring of anti-angiogenesis based therapy. (Refs. 9, 10) Although we and others have successfully developed various DOTA conjugated RGD peptides for multimodality imaging of integrin α_(v)β₃ expression. (Refs. 9, 10, 11, 31), the loss of ⁶⁴Cu from the chelator has lead to unfavorable high retention in liver, resulting in high background. Therefore, the choice of a more stable BFC is preferred.

Although some other novel BFCs have been developed and shown promise for use in copper-64 labeling (Refs. 2, 4, 12, 32), there is lack of adequate published data regarding the biological activity of these complexes. Some have high uptake in lung, liver and muscle, which may impair the detection of small lesions in the chest or/and abdominal regions. (Refs. 2, 4, 12, 32)

Recently, Sargeson and co-workers reported a new type BFC based on the sarcophagine (3, 6, 10, 13, 16, 19-hexaazabicyclo [6.6.6] icosane, Sar, FIG. 1.A-2) for preparation of ⁶⁴Cu-radiopharmaceuticals, (Refs. 2, 36) These ligands coordinate ⁶⁴Cu²⁺ within the multiple macrocyclic rings comprising the Sar cage structure, yielding stable complexes that are inert to the dissociation of the metal ion.

The caged-like BFC Sar ligands are able to selectively label ⁶⁴Cu²⁺ rapidly over a wider range of pH value under mild conditions. (Ref. 2) However, there are only a few reports that describe the complexation, stability and biodistribution of the ⁶⁴Cu complexes of the Sar ligand, and only (NH₂)₂-Sar (Diamsar) and 1-N-(4-aminobenzyl)-3, 6, 10, 13, 16, 19-hexaazabicyclo [6.6.6] icosane-1, 8-diamine (SarAr) have been reported as a BFC for the development of ⁶⁴Cu-radiopharmaceuticals. (Refs. 2, 13, 35, 36) Moreover, the relatively nontrivial and multi-step synthesis of Sar ligands may limit their future applications. (Ref. 4) However, the SARAR BFC utilizes the C-terminal for carboxylic acid for conjugation. This may be a disadvantage as the C-terminus is often found to be a crucial part for maintaining biological activity.

As such, there is a need for improved bifunctional chelators that can efficiently form stable complexes with metals, including Copper-64 under mild conditions.

There is also a need for new radiopharmaceuticals and imaging agents that are stable in vivo for imaging and other.

There is also a need for simplified methods for making bifunctional chelators.

BRIEF SUMMARY OF THE INVENTION

It is one object of the present invention to provide improved bifunctional chelators (BFCs) that form stable complexes with metals, including Copper-64, that are stable in vivo.

It is another object of the present invention to provide BFC/Targeting Moiety conjugates that specifically target biomolecules.

It is another object of the present invention to provide BFC/Targeting Moiety conjugate complexed with metals useful as imaging, therapeutic or contrast agents.

One embodiment of the present invention is directed to bifunctional chelators having the general formula

where A is a functional group selected from group consisting of an amine, a carboxylic acid, an ester, a carbonyl, a thiol, an azide and an alkene, and B is a functional group selected from the group consisting of hydrogen, an amine, a carboxylic acid, and ester, a carbonyl, a thiol, an azide and an alkene. In one preferred embodiment, A is a carboxylic acid, or a salt or ester thereof. Even more preferably, A is a carboxylic acid having the formula

and wherein R₁, R₂, R₃, and R₄ are independently selected from the group consisting of H, halogen, alkyl, alkoxy or alkene, or a salt or ester thereof. In a preferred embodiment, R₁, R₂, R₃, and R₄ are hydrogen.

In another preferred embodiment, the bifunctional chelators are

or a salt or ester thereof.

Another embodiment of the present invention is directed to bifunctional chelator/Targeting Moiety conjugates in which a bifunctional chelator is conjugated to a targeting moiety. In the conjugate, the bifunctional chelator is

where A is a functional group selected from group consisting of an amine, a carboxylic acid, an ester, a carbonyl, a thiol, an azide and an alkene, and B is a functional group selected from the group consisting of hydrogen, an amine, a carboxylic acid, and ester, a carbonyl, a thiol, an azide and an alkene, or a salt or ester thereof. In a preferred embodiment, the targeting moiety is selected from the group consisting of a peptide and antibody. For instance, the targeting moiety may be a peptide selected from the group consisting of a RGD, Asp-Gly-Glu-Ala (DGEA) (SEQ ID NO: 1), bombesin peptides (BBN), uPAR peptides, and other peptides with a lysine amine or N-terminal.

Another embodiment of the present invention is directed to a kit having a bifunctional chelator/Targeting Moiety conjugate with instructions for complexing a metal to the bifunctional chelator/Targeting Moiety conjugate.

The present invention is also directed new compositions comprising a bifunctional chelator conjugated to a Targeting moiety and complexed with a metal. These new compositions are useful as radiopharmaceuticals, therapeutic agents or contrast agents. In these compositions, the bifunctional chelator is

where A is a functional group selected from group consisting of an amine, a carboxylic acid, an ester, a carbonyl, a thiol, an azide and an alkene, and B is a functional group selected from the group consisting of hydrogen, an amine, a carboxylic acid, and ester, a carbonyl, a thiol, an azide and an alkene, or a salt or ester thereof. In these complexes, metal resides within the Sar cage and is bonded to one or more nitrogen. Preferably, the metal may be of ⁹⁰Y, Gd, ⁶⁸Ga, ⁵⁷Co, ⁶⁰Co, ⁵²Fe, ⁶⁴Cu or ⁶⁷Cu.

In one preferred embodiment, the present application is directed to a radiopharmaceutical comprising ⁶⁴Cu-AmBaSar-RGD, either alone or together with a carrier.

DESCRIPTION OF THE FIGURES

FIG. 1 is a chart depicting a procedure for the synthesis of the bifunctional chelator AmBaSar

FIG. 2 is a chart depicting a procedure for the synthesis of AmBaSar-RGD and labeled with Copper-64.

FIG. 3 is a representative ¹H-NMR spectra in D₂O of AmBaSar.

FIG. 4 is a representative HPLC chromatogram of AmBaSar.

FIG. 5 a representative chromatogram of crude AmBaSar-RGD using the semipreparative HPLC system.

FIG. 6 is a representative mass spectra of AmBaSar-RGD

FIG. 7 is representative radio-HPLC chromatogram of crude ⁶⁴Cu-AmBaSar-RGD using the analytical HPLC system described herein.

FIG. 8 shows a synthesis scheme for an improved method of synthesizing the bifunctional chelator AmBaSar.

FIG. 9 is a chart depicting a method for the radiosynthesis of ⁶⁴Cu-AmBaSar.

FIG. 10 is a representative chromatogram of crude ⁶⁴Cu-AmBaSar using analytical HPLC system

FIG. 11 is a graph showing the in vitro stability of ⁶⁴Cu-AmBaSar in PBS (pH 7.4) and FBS at 37° C.

FIG. 12 shows coronal sections of a microPET study of Balb/c mouse after single intravenous of ⁶⁴Cu-AmBaSar and ⁶⁴Cu-DOTA at 30 min and 2 hour. K=Kidney; L=Liver; B=Bladder.

FIG. 13 is a graph showing the biodistribution of ⁶⁴Cu-AmBaSar and ⁶⁴Cu-DOTA in Balb/C mice after 2 h postinjection.

FIG. 14 is a chart comparing the chemical structures of ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD.

FIG. 15 is a graph showing the in vitro stability of ⁶⁴Cu-AmBaSar-RGD in PBS (pH 7.4), FBS, and mouse serum for incubation under 37° C. for 3, 18, and 24 h.

FIG. 16 is a graph showing that the U87MG cell uptakes of ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD at 0.5, 1, and 2 h in the absence/presence of excess amount of cyclic RGD

FIG. 17 is a MicroPET study of U87MG tumor-bearing mice showing: (A) The coronal images of nude mice bearing U87MG tumor at 1, 2, 4, and 20 h p.i. of ⁶⁴Cu-AmbaSar-RGD and ⁶⁴Cu-DOTA-RGD; and (B) Time activity curves of ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD in U87MG tumor, liver, and kidneys (n=3). Tumors are indicated by arrows.

FIG. 18 is a MicroPET imaging study of ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD on U87MG xenograft mouse model at 2 h p.i. with/without a blocking dose of cyclic RGD: (A) microPET coronal images; (B). Quantitative analyses of microPET imaging of U87MG tumor, muscle, liver, and kidneys (n=3). Arrows indicate the tumor positions.

FIG. 19 shows (A) a graph showing biodistribution data for ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD in mice bearing U87MG glioma xenografts (mean±SD, n=3) at 20 h p.i.; and (B) a graph showing the ratios of tumor to main organs uptake of ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD.

FIG. 20A and FIG. 20B. FIG. 20A, Metabolic stability of ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD in mouse blood sample and in liver, kidney and U87 MG tumor homogenates at 1 h post injection. FIG. 20B, The HPLC profiles of pure ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD (Standard) are also shown.

FIG. 21 is a chart showing a synthetic method for the preparation of thiol and carboxylate functionalized BFCs according to the present invention.

FIG. 22 is a chart showing a synthetic method for the preparation of DiBaSar according to the present invention.

DETAILED DESCRIPTION OF THE INVENTION

One embodiment of the present invention is directed to a class of versatile Sarcophagine based bifunctional chelators containing a hexa-aza cage for labeling with metals having either imaging, therapeutic or contrast applications radiolabeling and one or more linkers (A) and (B). The compounds of the present invention have the general formula

where A is a functional group selected from group consisting of an amine, a carboxylic acid, an ester, a carbonyl, a thiol, an azide and an alkene, and B is a functional group selected from the group consisting of hydrogen, an amine, a carboxylic acid, and ester, a carbonyl, a thiol, an azide and an alkene. Suitable linker group A and B should be of sufficient length (˜6 atom lengths) and should incorporate a reactive group that can be readily attached to a range of target agents, but not interfere with efficient and selective complexation of a metal ion like Cu²⁺ to the sarcophagine cage, as well as the target agent's biological activity. (Ref. 16)

In one embodiment of the present invention, linkers A or B, or both, may preferably be a carboxylic acid of the following formula:

Where R₁, R₂, R₃, and R₄ are independently selected from the group consisting of H, halogen, alkyl, alkoxy or alkene.

In another embodiment of the present invention, the bifunctional chelators are sarcophagine based compositions, referred to herein as AmBaSar and DiBaSar, having the having the following structure:

The bifunctional chelators may be conjugated to a targeting moiety as BFC/Targeting Moiety conjugates that specifically target a range of biological molecules. In two separate embodiments, the targeting moiety is a peptide or an antibody.

For instance, the pendant carboxylate group of carboxylic acid (ROOH) functionalized BFC, including AmBaSar and DiBaSar, can be directly conjugated to the amine of lysine in biological molecules, which permit the development of new biomolecule-based ⁶⁴Cu-radiopharmaceuticals. More specifically, the BFC's can be used to directly conjugate targeting peptides (Z) through the formation of an amide bond with the peptide to form BFC peptide conjugates of the following structure:

where Z is a targeting peptide containing lysine.

Examples of the peptides to which AmBaSar, and other carboxylic acid based BFCs may be conjugated include, but are not limited to, the small cyclic peptide Arg-Gly-Asp (RGD). Asp-Gly-Glu-Ala (DGEA) (SEQ ID NO: 1), bombesin peptides (BBN), uPAR peptides, and other peptides with a lysine amine or N-terminal. Sar-DGEA is directly conjugated to the Sar cage without functionalization by solid or liquid phase methods well known in the art. In vitro and in vivo evaluation of the AmBaSar-RGD demonstrates the potential of the BFC's of this invention for preparation of a range of radiopharmaceuticals.

The BFC and the BFC/Targeting Moiety conjugates of the present invention may be complexed with a range of metals by known methods to produce radiopharmaceuticals for imaging or therapy. The use of the word “metal” or “metals” throughout this specification should be understood to include metal ions and their salts. The BFC and the BFC/Targeting Moiety conjugates may also be combined with paramagnetic metals for use as contrast agents in MR imaging or with these or other metals for CT scanning applications. Examples of suitable metal ions for use in the present invention include, but are not limited to, ⁹⁰Y, Gd, ⁶⁸Ga, ^(57/60)Co, ⁵²Fe, ^(64/67)Cu In the Metal-BFC and Metal-BFC/Targeting Moeity complexes of the present invention, the metal resides within the Sar cage bound to the nitrogen of the Sar Cage as shown in FIG. 14 for ⁶⁴Cu-AmBaSar-RGD.

In order to form the radiopharmaceuticals in accordance with the present invention, the BFC/Targeting Moiety conjugates complexed with a metal may be dispersed or dissolved in a suitable carrier in appropriate concentrations and delivered to the patient in appropriate doses. Preferred routes of delivery are oral, injection, or infusion. The identity of the carrier is not particularly limited so long as the radiopharmaceutical is stable in the carrier. Suitable carriers for use in connection with the present invention include Saline (0.9%), Phosphate Buffer Solution, or Ethanol solution (<8%). The carrier may optionally include HSA protein, synthetic polymers, dendrimers, cyclodextron et al. The active species should be delivered in an amount effective to produce the desired effect but below the level where there is unacceptable toxicity. When used in solution, concentration of active species in the carrier should be sufficiently high to produce the desired effect but below the level where there is significant toxicity. Typical concentrations for imaging applications are approximately in the range of 1-20 mCi/mL.

In one example of the present invention, AmBaSar is conjugated to the small cyclic Arg-Gly-Asp (RGD) peptide, and subsequently labeled with ⁶⁴Cu, to provide a new PET probe ⁶⁴Cu-AmBaSar-RGD for imaging the α_(v)β₃ integrin receptor. ⁶⁴Cu-AmBaSar-RGD has the following formula:

Another embodiment of the present invention is directed to new radiopharmaceuticals comprising ⁶⁴Cu-AmBaSar-RGD. ⁶⁴Cu-AmBaSar-RGD is obtained with high radiochemical yield (≧95%) and purity (≧99%) under mild conditions (pH 5.0˜5.5, 23˜37° C.) in less than 30 min. In order to form the radiopharmaceuticals in accordance with the present invention, ⁶⁴Cu-AmBaSar-RGD may be dispersed or dissolved in a suitable carrier in appropriate concentrations delivered to the patient in appropriate doses orally, or by injection, infusion or, where possible. Suitable carriers for use in connection with ⁶⁴Cu-AmBaSar-RGD include Saline (0.9%), Phosphate Buffer Solution, or Ethanol solution (<8%). Carrier may include HSA protein, synthetic polymers, dendrimers, cyclodextron et al. The concentration of ⁶⁴Cu-AmBaSar-RGD in the carrier should be sufficiently high to produce sufficient signal to permit tracking and/or imaging of the ⁶⁴Cu-AmBaSar-RGD within the patient after deliver but below the level where there is significant toxicity. Suitable concentrations for the ⁶⁴Cu-AmBaSar-RGD are preferably 1˜20 mCi/mL.

In another embodiment of the present invention, a kit comprises a BFC/Targeting Moiety conjugate together with instructions for forming the metal complex with the BFC/Targeting Moiety conjugate.

The BFC, BFC/Targeting Moiety and the BFC/Targeting Moiety conjugate complexed with a metal may each be in the form of a pharmaceutically acceptable salts or ester form. Any carboxylic acid described herein is also understood to encompass pharmaceutically salt or esters of the carboxylic acid.

Metabolic studies support the observation that ⁶⁴Cu-AmBaSar-RGD is more stable in vivo than ⁶⁴Cu-DOTA-RGD. In vitro and in vivo evaluations of the ⁶⁴Cu-AmBaSar-RGD demonstrate its improved stability compared with the established tracer ⁶⁴Cu-DOTA-RGD. For in vitro studies, the radiochemical purity of ⁶⁴Cu-AmBaSar-RGD was more than 97% in the PBS or FBS and 95% in mouse serum after 24 hr incubation. The log P value of ⁶⁴Cu-AmBaSar-RGD was −2.44±0.12. For in vivo studies, ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD have demonstrated comparable tumor uptake at selected time points based on microPET imaging. The integrin α_(v)β₃ receptor specificity was confirmed by blocking experiments for both tracers. Compared with ⁶⁴Cu-DOTA-RGD, ⁶⁴Cu-AmBaSar-RGD exhibits much lower liver accumulation in both microPET imaging and biodistribution studies.

Abbreviations and Nomenclature

The IUPAC names for the cage ligands of the present invention and metal complexes of the cage compounds are long and complicated. The names for the ligands described or discussed herein are abbreviated as follows:

-   3, 6, 10, 13, 16, 19-hexaazabicyclo [6.6.6] icosane is referred to     “sarcophagine”, or “Sar”; -   1, 8-Diamine-3, 6, 10, 13, 16, 19-hexaazabicyclo [6.6.6] icosane is     referred to as “Diamsar”; -   1-N-(4-aminobenzyl)-3, 6, 10, 13, 16, 19-hexaazabicyclo [6.6.6]     icosane-1, 8-diamine is referred to as “SarAr”; -   Methyl 4-((8-amino-3, 6, 10, 13, 16, 19-hexaazabicyclo [6.6.6]     icosane-1-ylamino) methyl) benzoate is referred to as “AmMBSar”; and -   4-((8-amino-3, 6, 10, 13, 16, 19-hexaazabicyclo [6.6.6]     icosane-1-ylamino) methyl) benzoic acid is referred to as “AmBaSar”; -   1,4,7,10-tetraazacyclododecane-N,N′,N″,N″′-tetraacetic acid is     referred to as DOTA, and -   1,4,8,11-tetraazacyclotetradecane-N,N′,N″,N″′-tetraacetic acid is     referred to as TETA.

Unless otherwise indicated, complexes described herein are named using a nomenclature which represents these M-hexaamine cage complexes by “M-(A, Bsar)”, where M represents metal ion, and A and B are the substituents in the 1- and 8-positions of the Sar cage:

-   (1, 8-Dinitro-Sar) cobalt(III) trichloride is represented by the     chemical formula [Co(DiNosar)]Cl₃; -   (1, 8-Diamine-Sar) cobalt(III) pentachloride is represented by the     chemical formula [Co(DiAmSar)]Cl₅; -   (1, 8-Diamine-Sar) copper(II) tetrachloride is represented by the     chemical formula [Cu(DiAmSar)]Cl₄; -   (1-amine, 8-(aminomethyl) 4′-methylbenzoate-Sar) copper(II) is     represented by the chemical formula [Cu(AmMBSar)]²⁺; -   (1-amine, 8-(aminomethyl)-benzoic acid-Sar) copper(II) is     represented by the chemical formula [Cu(AmBaSar)]²⁺; -   (1, 8-(aminomethyl) 4′-methylbenzoate-Sar) copper(II) is     [Cu(DiAMBSar)]²⁺.

Design, Synthesis, and Characterization of Bifunctional Chelator AmBaSar

In order to design a suitable bifunctional chelator for ⁶⁴Cu labeling and conjugating with RGD, it was necessary to modify the linkage of diamsar. The aromatic amine of SarAr can be replaced with an aromatic carboxyl, which can conjugate a cyclic peptide containing the RGD motif in addition to a lysine for conjugating to the chelator, to form BFC AmBaSar. AmBaSar can efficiently label ⁶⁴Cu²⁺ due to the provision of a three-dimensional hexa-aza cage which increases thermodynamic and kinetic stability to complex ⁶⁴Cu²⁺ or other metal ions, while allowing the aromatic linker with carboxyl acid group to conjugate with the amine of lysine in the cyclic peptide containing the RGD motif. The AmBaSar-RGD can be used to form new nuclear, MRI, and optical probes by complexion with other appropriate metal radioisotopes or paramagnetic metal ions using similar preparations. Appropriate metals include, but are not limited to ⁹⁰Y, Gd, ⁶⁸Ga, ^(57/60)Co, ⁵²Fe and ^(64/67)Cu.

AmBaSar can be reacted with a variety of peptides or biomolecules, since the chemistry for conjugating AmBaSar to other peptides is similar to that described for the cyclic peptide RGD. The identity of the peptides is not particularly limited as long as pendant carboxylate group or carboxylic acid group of the AmBaSar chelator be directly conjugated to an amine of a lysine or N-terminal in the peptide. Preferably however, the peptide is to which AmBaSar is reacted is one that targets a specific biomolecule. Other peptides include, but are not limited to, Asp-Gly-Glu-Ala (DGEA) (SEQ ID NO: 1), bombesin peptides (BBN), uPAR peptides, and other peptides with a lysine amine or N-terminal.

An efficient synthesis of AmBaSar is shown in FIG. 1. The degree of hydration of the synthesized compounds is dependent on the method of purification. FIG. 1, Compounds 1˜4 may be prepared based on methods described in the literature using cobalt complexes as starting materials, (Refs. 14, 15) However, the reported syntheses of compound 1˜4 are incomplete and with compounds not fully characterized. The comprehensive synthetic methods and full characterization of these compounds are disclosed herein.

In brief, and as shown in FIG. 1-1, tris(ethylenediamine)cobalt(III) chloride initiates the encapsulation process using the reactive nucleophile nitromethane and formaldehyde in alkaline solution at room temperature to form a hexa aza cage containing Co(III) compound 1, which was then reduced with zinc dust in acid solution to give the very stable Co(III) diamsar complex 2. The Co(III) ion of compound 2 can be removed by reduction with high concentrations of hydrochloric or hydrobromic acid at high temperatures (130˜150° C.) or excess cyanide ion to yield the free cage. Here we used excess cyanide ion to remove the metal ion in compound 2 to form compound 3 in good yield (58.5%). The six nitrogen donor atoms of the hexa aza cage allows strong binding to many metal ions, such as Cu²⁺, so compound 3 was easy to complex with metal ion Cu²⁺, yielding compound 4 under weak acid conditions. The compounds 1˜4 were characterized by elemental analysis, MS and ¹H-NMR, the results are consistent with literature reports. (Refs. 14, 15.)

It is difficult to functionalize the apical primary amines of diamsar 3 (FIG. 1) directly because there are 2 primary and 6 secondary amines in diamsar, which potentially could create many by-products and difficulty during purification. The initial formation of copper(II) complex of diamsar 4 (FIG. 1) ties up the 6 secondary amines of diamsar, and also permit the tracking of the resultant Cu(II) complexes on the ion exchange columns. (Ref. 16.) Structural studies have confirmed that it is possible to exploit the relatively low nucleophilicity of the Cu(II) complex of diamsar in acylation and alkylation reactions leading to a variety of functionalized cage amine complexes. (Refs. 17, 18). The hydride reducing agent sodium cyanoborohydride (NaBH₃CN) is used for reduction due to its stability in relatively strong acid solutions (about pH 3), its solubility in hydroxylic solvents such as ethanol, and its different selectivities at different pH values. At pH 3˜4 it reduces the imine to an amine efficiently, while this reduction becomes very slow at higher pH values. (Ref. 19) The reducing reaction of the cage amine of compound 4 with aromatic methyl 4-formylbenzoate under NaBH₃CN ethanol acid solution yields aromatic functionalization of the cage amine compound 5 and the by-product bis-4-formylbenzoate diamsar complex. This reaction took a significant amount of time (4 days) and yield was 27.9% due to low nucleophilicity. Separation was carried out by ion exchange chromatography. Compound 6 was achieved by demetallation of compound 5, followed by alkaline hydrolysis to produce the target compound 7 AmBaSar according to the reported method. (Ref. 20)

AmBaSar Conjugating Cyclic Peptide RGD and ⁶⁴Cu Radiolabeling:

AmBaSar contains one carboxyl group and an inactive primary amine, which means that it is a mono-functional molecule that can react with a cyclic peptide containing the RGD motif in addition to a lysine for conjugating to the chelator. Literature methods may be used for conjugation of the cyclic RGD with AmBaSar and preparing ⁶⁴Cu radiolabeled conjugates. (Refs. 6, 21, 22)

FIG. 2 is a chart showing the method for AmBaSar conjugating cyclic RGD and ⁶⁴Cu radiolabeling. The cyclic RGD conjugate AmBaSar-RGD was synthesized in 80% yield and purified by semipreparative HPLC. Analytical HPLC found the retention time of AmBaSar-RGD to be 3.8 min, whereas cyclic RGD peptide eluted at 25 min under the same condition. AmBaSar-RGD was analyzed by mass spectrometry, found m/z=1049.3 for [M+H]⁺ (M=C₅₀H₈₀N₁₆O₉) and 1089.7 for [M+K]⁺.

In another embodiment of the present invention, the peptide-chelator conjugate AmBaSar-RGD can be complexed with ⁶⁴Cu to form a new PET tracer for imaging the α_(v)β₃ integrin receptor. AmBaSar-RGD was labeled with ⁶⁴Cu in 0.1 M ammonium acetate (pH 5.0) solution at room temperature (25° C.) for 1 h. The free ⁶⁴Cu-acetate was eluted at 3.2 min, while ⁶⁴Cu-AmBaSar-RGD was eluted at 15.8 min by analytical HPLC, which was confirmed by cold Cu-AmBaSar-RGD. The radiochemical yield obtained was ≧80% and the radiochemical purity was ≧95%.

Experimental

Methods and Materials:

¹H NMR spectra were obtained using a Varian Mercury 400 MHz instrument (USC NMR Instrumentation Facility), and the chemical shifts were reported in ppm on the δ scale relative to an internal TMS standard. Microanalyses for carbon, hydrogen, nitrogen and chlorine, cobalt, copper were carried out by the Columbia Analytical Services, Inc (Tucson, Ariz.). Mass spectra using LC-MS were operated by the Proteomics Core Facility of the USC School of Pharmacy. Thin-layer chromatography (TLC) was performed on silica gel 60 F-254 plates (Sigma-Aldrich) using a mixture solution of 70% MeOH and 30% aqueous NH₄OAc (NH₄OAc solution is 20% by weight) as the mobile phase. Ion-exchange chromatography was performed under gravity flow using Dowex 50WX2 (H⁺ form, 200-400 mesh) or SP Sephadex C25 (Na⁺ form, 200-400 mesh) cation exchange resins. All evaporations were performed at reduced pressure (ca. 20 Torr) using a Büchi rotary evaporator.

HPLC was accomplished on two Waters 515 HPLC pumps, a Waters 2487 absorbance UV detector and a Ludlum Model 2200 radioactivity detector, operated by Waters Empower 2 software. Purification of the conjugate AmBaSar-RGD was performed on a Phenomenex Luna C18 reversed phase column (5 μm, 250×10 mm); the flow was 3.2 mL/min, with the mobile phase solvent A (12% acetonitrile in water), and the absorbance monitored at 254 nm. The analytical HPLC was done on a Phenomenex Luna C18 reversed phase column (5 μm, 250×4.6 mm) and monitored using a radiodetector and UV at 218 nm. The flow was 1.0 mL/min, with the mobile phase starting from 99% solvent B (0.1% TFA in water) and 1% solvent C (0.1% TFA in acetonitrile) (01 min) to 70% solvent B (0.1% TFA in water) and 30% solvent C (0.1% TFA in acetonitrile) (1˜30 min).

All reagents and solvents were purchased from Sigma-Aldrich Chemicals (St. Louis, Mo., USA) and used without further purification unless otherwise stated. N-hydroxysulfosuccinimide sodium salts (SNHS) and N-ethyl-N-(3-dimethylaminopropyl) carbodiimide hydrochloride (EDC.HCl) were obtained from the Sigma-Aldrich Chemical Co. The cyclic RGDyK peptide was purchased from Peptides International, Inc (Louisville, Ky., USA). ⁶⁴CuCl₂ was purchased from MDS Nordion (Vancouver, BC, Canada). Water was purified using a Milli-Q ultra-pure water system from Millipore Corp. (Milford, Mass., USA).

Experimental: AmBaSar Synthesis and Characterization Synthesis of [Co(DiNoSar)]Cl₃ (1)

To a solution of tris(ethylenediamine)cobalt(III) chloride dehydrate (1.2 g, 3.0 mmol) in water (4.0 mL) was added nitromethane (0.7 g, 12 mmol) and aqueous formaldehyde (37%, 2.4 g, 30 mmol). The resulting solution was cooled to 4° C. on an ice-water bath. Aqueous NaOH (4.0 M, 3.0 mL) was cooled to 4° C. and mixed with the resulting solution above. The combined solution was stirred on ice-water bath where it rapidly turned deep violet-brown from the initially orange color, and the reaction temperature was allowed to raise to room temperature 23-25° C. After 90 min, the reaction was quenched by the addition of HCl (6.0 M, 2.0 mL). The orange precipitate formed was collected by filtration after cooling on ice for 2 h, washed with methanol, and dried to provide 1 (1.46 g, 90.2%). ¹H-NMR (D₂O): δ 3.55-3.65 (d, 6H, NCCH₂N); 3.15-3.35 (d, 6H, NCCH₂N); 3.00-3.10 (d, 6H, NCH₂CH₂N); 2.55-2.65 (d, 6H, NCH₂CH₂N). MS: Calcd for C₁₄H₃₁CoN₈O₄[M+1-3HCl]⁺ m/z 431.2, found 431.5. Elemental analysis calculated for C₁₄H₃₀Cl₃CoN₈O₄, requires C, 31.15; H, 5.60; N, 20.76; Cl, 19.71; Co, 10.92. Found: C, 30.90; H, 5.46; N, 20.13; Cl, 20.80; Co, 10.70.

Synthesis of [Co(DiAmSar)]Cl₅.H₂O (2)

[Co(DiNoSar)]Cl₃ (2.0 g, 3.7 mmol) was dissolved in deoxygenated water (100 mL) under N₂ atmosphere. Zinc dust (2.3 g, 35 mmol) was added into the solution with stirring for 5 min, followed by addition of HCl (6 M, 15 mL) dropwise. The resulting solution continued to stir for an additional 60 min under N₂ atmosphere. The N₂ flow was stopped and 30% H₂O₂ (1.0 mL) was added. The resulting solution was warmed for 15 min on 75° C. water bath, then cooled and placed on a Dowex 50WX2 cation exchange column and washed with water (120 mL), followed by HCl (1.0 M, 120 mL). The complex was then eluted with HCl (3.0 M, 400 mL) and the yellow eluate was collected and dried under vacuum to yield 2 (1.78 g. 87%). ¹H-NMR (D₂O): δ 3.30-3.10 (m, 12H, NCCH₂N); 2.50-2.65 (m, 12H, NCH₂CH₂N). MS Calcd for C₁₄H₃₅CoN₈ [M+1-5HCl-H₂O]³⁰ m/z 371.2, found 371.7. Elemental analysis calculated for C₁₄H₃₈Cl₅CoN₈O, requires C, 29.46; H, 6.71; N, 19.63; Cl, 31.06; Co, 10.33. Found: C, 29.06; H, 6.73; N, 19.04; Cl, 25.30; Co, 9.50.

Synthesis of Diamsar.5H₂O (3)

Co(DiAmSar)]Cl₅.H₂O (3.58 g, 6.3 mmol), NaOH (0.58 g, 14.5 mmol, sufficient to neutralize the protonated primary amino groups) and Cobalt(II) chloride hexahydrate (1.6 g, 6.4 mmol) were dissolved in deoxygenated water (50 mL) under nitrogen. Sodium cyanide (5.60 g, 114 mmol) was added to the resulting solution. The reaction mixture was heated to 70° C. being stirred under nitrogen until the solution had become almost colourless (overnight). This final solution was taken to dryness under vacuum, with the residue extracted with boiling acetonitrile (3×25 mL). The total extract was filtered, reduced under vacuum to a white solid, and cooled to −10° C. to precipitate white crystals of the product. Drying in vacuo provided 3 (1.72 g, 58.5%). mp 91˜94.0° C. ¹H-NMR (D₂O): δ 2.51 (s, 12H, NCCH₂N); 2.42 (s, 12H, NCH₂CH₂N). MS Calcd for C₁₄H₃₅N₈ [M+1-5H₂O]⁺ m/z 315.3, found 315.8. Elemental analysis calculated for C₁₄H₄₄N₈O₅, requires C, 41.56; H, 10.96; N, 27.70, Found: C, 41.53; H, 10.28; N, 27.12.

Synthesis of [Cu(DiAmSar)]Cl₄.5H₂O (4)

CuCl₂.2H₂O (0.17 g, 1.0 mmol), was dissolved in 10 mL water, following added 3 (0.41 g, 1.0 mmol). The solution was acidified to pH=4.0 with HCl (0.1 M), and stirred overnight. Evaporation on heating yielded a blue precipitate. The blue solid was cooled, filtered, and washed with ethanol (5 mL×3), and dried, yielding a blue crystalline product 4 (0.53 g, 97%). ¹H-NMR (D₂O): δ 3.20 (s, 12H, NCH₂CH₂N); 2.90 (s, 12H, NCCH₂N). MS Calcd for C₁₄H₃₃CuN₈ [M+1-4HCl-5H₂O]⁺ m/z 376.2, found 376.0. Elemental analysis calculated for C₁₄H₄₆Cl₄CuN₈O₅, requires C, 27.48; H, 7.58; N, 18.31; Cl, 23.17, Cu, 10.38, Found: C, 27.72; H, 7.17; N, 17.87; Cl, 22.40, Cu, 9.71.

Synthesis of [Cu(AmMBSar)](CH₃COO)₂.5H₂O (5)

[Cu(DiAmSar)]Cl₄.5H₂O (0.73 g, 1.2 mmol) was dissolved in dry ethanol (30 mL), followed by addition of methyl 4-formylbenzoate (0.28 g, 1.7 mmol), dried/activated 4 Å molecular sieves (1.0 g) and glacial acetic acid (60 μL). The resulting solution was stirred for 3 h under argon gas, followed by addition of sodium cyanoborohydride (0.82 g, 14 mmol). The reaction mixture continued to stir under argon gas for 4 days at room temperature 20˜25° C. The mixture was filtered, and filtrate was evaporated to dryness and extracted with ethyl acetate (15 mL×3), dried and then diluted to 300 mL. It was placed onto a SP Sephadex C25 column and eluted with sodium citrate (0.1 M, 400 mL) and a wide blue band formed. Increasing the sodium citrate concentration (0.3 M, 500 mL) resulted in three blue bands eluting in order as [Cu(diamsar)]²⁺, [Cu(AmMBSar)]²⁺ (compound 5), and [Cu(DiAMBSar)]²⁺ by TLC monitoring. The second band eluate (compound 5 solution, 100 mL) was isolated and diluted with water (10 fold, 1.0 L), and placed onto another SP Sephadex C25 column. A single blue band eluted with sodium acetate (1.0 M, 200 mL), was evaporated to dryness and the residue extracted with 2-propanol (50 mL×3). Fine white crystals of sodium acetate were separated, filtered and the process of evaporation and extraction repeated 3 times. The final residue was dried in vacuo to a dark blue solid 5 [Cu(AmMBSar)](Ac)₂.5H₂O (246.5 mg, 27.9%). ¹H-NMR (D₂O): δ 8.0-7.9 (d, 2H, aromatic); 7.48-7.42 (d, 2H, aromatic); 4.70 (s, 3H, OCH₃); 4.02 (s, 2H, CH₂—Ar); 3.54-3.30 (m, 12H, NCH₂CH₂N); 2.93-2.78 (m, 12H, NCCH₂N). MS Calcd for C₂₃H₄₃CuN₈O₂[M+1-2HAc-5H₂O]⁺ m/z 526.3, found 526.8.

Synthesis of AmMBSar (6)

Sodium borohydride (150 mg) was dissolved in 0.4 mL water and stirred under a nitrogen atmosphere, following addition of Pd/C (60 mg) in 1.0 mL water. Compound 5 (164 mg) was dissolved in sodium hydroxide (3 mL; 1% NaOH) and added dropwise to the above mixture solution. Stirring was continued under nitrogen at 25° C. until the color turned from blue to clear. The resulting solution was filtered (0.22 μm) and the filtrate collected in an ice-cooled glass vial. Concentrated hydrochloric acid was added dropwise (50 μL) to the cooled solution until gas evolution ceased (˜450 μL, HCl). The solution was acidified to pH 4˜6, and then dried under vacuum to provide AmMBSar, 6 (56 mg, 47.6%). ¹H-NMR (D₂O): δ 7.97-7.92 (d, 2H, aromatic); 7.50-7.45 (d, 2H, aromatic); 4.65 (s, 3H, OCH₃); 4.08 (s, 2H, CH₂—Ar); 3.45-3.20 (m, 12H, NCH₂CH₂N); 3.12-2.98 (m, 12H, NCCH₂N); 1.98-1.85 (m, 9H, NH). MS Calcd for C₂₃H₄₂N₈O₂ [M+1]⁺ m/z 463.0, found 462.3.

Synthesis of AmBaSar (7)

Compound 6 (46.2 mg, 0.1 mmol) was dissolved in methanol (3 mL) and water (1.0 mL), followed by addition of NaOH (1.5 mL, 0.1 M). The resulting solution was refluxed and stirred for 5 h, then neutralized with HCl (1.0 M) to pH 6˜7. Drying the solution under reduced pressure formed solids, which were dissolved with hot MeOH (3×2 mL). The total extract was filtered and dried under vacuum to yield AmBaSar, 7 (36 mg, 80.2%). ¹H-NMR (D₂O): δ 7.76-7.67 (m, 2H, aromatic); 7.45-7.37 (m, 2H, aromatic; 3.66 (s, 2H, NCH₂C) 3.26-3.04 (m, 12H, NCCH₂N); 2.99-2.84 (m, 12H, NCH₂CH₂N); 1.84-1.77 (m, 9H, NH). MS Calcd for C₂₃H₄₁N₈O₂ [M+1]⁺ m/z 449.3, found 449.7. A typical ¹H-NMR spectra of AmBaSar in D2O is shown in FIG. 3. A Typical HPLC chromatogram of AmBaSar using the Analytical HPLC system is shown in FIG. 4.

Synthesis of Other Carboxylic Acid Functionalized Sar Based Bifunctional Chelators

Although the methodology for functionalizing the apical amine has been described primarily with respect to AmBaSar, Sar may be functionalized with other carboxylic acids by reacting with the compounds that have an aldehyde on one side and the Methoxyl ester on the other. These two groups could located at different positions of an aromatic system (including those with hetero-atoms), aliphatic system (including those with double or triple bonds), or the combination of those two.

Synthesis of Carboxylate and Thiol Functionalized Sar Based Bifunctional Chelators

Using methods analogous to the preparation of AmBaSar, the carboxylate and thiol functionalized Sar cage is synthesized by a method shown in FIG. 21. Starting from the mono-substituted Sar cage and commercially available agents, a bifunctional linker with protected thiol and carboxylate groups is obtained. After the removal of the Co metal and deprotection, the carboxylate and thiol functionalized Sar cage is obtained. Various linkers may also be introduced to this Sar cage agent.

Synthesis of DiBaSar and Functionalized Sar Based Bifunctional Chelators Having Carboxylic Acid Groups at Both Apical Amines

DiBaSar and Sar based structures functionalized with carboxylic acids at both apical amines may be synthesized by a synthetic procedure described in FIG. 22

Experimental: AmBaSar Conjugating Peptide RGD and Radiolabeling Synthesis of AmBaSar-RGD (8, FIG. 2)

AmBaSar was activated by EDC at pH 5.5 for 30 min (4° C.), with a molar ratio of AmBaSar:EDC:SNHS=5:5:4. Typically, 15.0 mg of AmBaSar (30 μmol) was dissolved in 500 μL of water. Separately, 5.76 mg of EDC (30 μmol) was dissolved in 500 μL of water. The two solutions were mixed, and 0.1 M NaOH (250 μL) was added to adjust the pH to 4.5. SNHS (5.2 mg, 24 μmol) was then added to the stirring mixture on an ice-bath, followed by 0.1 M NaOH (50 μL) to finalize the pH to 5.4. The reaction was allowed to stir for 30 min at 4° C. The theoretical concentration of active ester AmBaSar-OSSu was calculated to be 24 μmol. Cyclic RGD peptide (2.5 mg, 4.0 μmol) dissolved in 500 μL (5.0 mg/mL) of water was cooled to 4° C. and added to the AmBaSar-OSSu reaction mixture. The pH was adjusted to 8.6 with 0.1 M NaOH (280 μL). The reaction was allowed to proceed overnight at room temperature (20˜25° C.). The AmBaSar-RGD conjugate was purified by semipreparative HPLC. A representative chromatogram of the AmBaSar-RGD is shown in FIG. 5. The peak containing the RGD conjugate was collected, lyophilized, and dissolved in water at a concentration of 1.0 mg/mL for use in radiolabeling reactions. A mass spectra of AmBaSar-RGD is shown in FIG. 6.

Synthesis of [Cu-AmBaSar-RGD](Ac)₂.2HAc

The AmBaSar-RGD (1.0 mg) was dissolved in 0.5 mL of a 0.1 M ammonium acetate/0.80 mM copper (II) acetate solution. The mixture was stirred at 37° C. for 40 min and allowed to cool to room temperature. The crude Cu-AmBaSar-RGD solution was purified and quantified by HPLC. MS Calcd for C₅₈H₉₄N₁₆O₁₇Cu [M+1]⁺ m/z 1352.0, found 1351.9.

Radiolabeling of ⁶⁴Cu-AmBaSar-RGD

[⁶⁴Cu]Acetate (⁶⁴Cu(OAc)₂) was prepared by adding 111 MBq (3 mCi) of ⁶⁴CuCl₂ in 0.1 M HCl into an 1.5 mL microfuge tube containing 300 μL 0.1 M ammonium acetate (pH 5.0), followed by mixing using a mini vortex and incubating for 15 min at room temperature. The AmBaSar-RGD (1-2 μg in 100 μL 0.1 M ammonium acetate) was labeled with ⁶⁴Cu(OAc)₂ by addition of 1-3 mCi of ⁶⁴Cu. The chelation reaction was performed in 0.1 M sodium acetate buffer, pH 5.0, for 60 min at room temperature (23˜25° C.). Labeling efficiency was determined by HPLC. ⁶⁴Cu-AmBaSar-RGD was purified by radio-HPLC. The elute was evaporated and the activity reconstituted in saline, followed by passage through a 0.22 μm Millipore filter into a sterile dose vial for use in animal experiments. A representative radio-HPLC chromatogram of ⁶⁴Cu-AmBaSar-RGD is shown in FIG. 7.

Improved Synthesis of AmBaSar

Another embodiment of the present invention is directed to an improved synthetic route of AmBaSar. The improved synthesis of the BFC AmBaSar is shown in FIG. 8. In this new synthetic route, AmBaSar is obtained in only four steps starting from Co(DiAmSar)]Cl₅ (1). As shown in FIG. 8, Compound 1 was transformed to the 3Cl⁻ salt by neutralizing the protonated primary amino groups with NaOH, which was then converted to the tetraphenylborate salt compound 2 by anion exchange of [Co(DiamSar)]Cl₃ with sodium tetraphenylborate (NaBPh₄) in aqueous solution. (Ref. 24) The coupling of the aldehyde to the amine of compound 2 yielded aromatic functionalization of the cage compound 3 Co(AmBMSar) complex. This reaction was carried out under dehydrating and refluxing conditions before adding the reducing agent according to literature method. (Ref. 24) Molecular sieves 4 Å were employed to remove the water produced in the formation of the iminium ion. Compared with the Cu complex (27.9% yield), we also observed an increased yield (39.1% yield) in this step, which could be partially attributed to the preferable solubility of the tetraphenylborate salt compared with the chloride salt in methanol. We also found that AmBaSar could be made in two ways from compound 3. One method was similar to that discussed herein, where the Co(III) ion of compound 3 was removed by excess cyanide ion to yield the free cage compound 5 AmBMSar, which then was hydrolyzed to produce the target compound 6 AmBaSar. Another method employed alkaline hydrolysis of compound 3 first, with subsequent removal of cobalt ion to yield the AmBaSar (6).

This improved synthesis of AmBaSar shortens synthetic steps and simplifies purification. The improved synthesis also simplified the separation process and increased the yield. The overall yield was increased to about 6.0±0.2% (n=6) compared with the original 4.7% by using tris(ethylenediamine)cobalt(III) chloride dehydrate as starting material.

Materials.

All reagents and solvents were purchased from Sigma-Aldrich Chemicals (St. Louis, Mo., USA) and used without further purification unless otherwise stated. DOTA was purchased from Macrocyclics (Dallas, Tex., USA). ⁶⁴CuCl₂ was ordered from MDS Nordion (Vancouver, BC, Canada). Compound 1 (Co(DiAmSar)]Cl₅.H₂O) was prepared as described herein. Water was purified using a Milli-Q ultra-pure water system from Millipore Corp. (Milford, Mass., USA).

General Methods:

¹H NMR spectra were obtained using a Varian Mercury 400 MHz instrument (USC NMR Instrumentation Facility), and the chemical shifts were reported in ppm on the δ scale relative to an internal TMS standard. Mass spectra using LC-MS were provided by the Proteomics Core Facility of the USC School of Pharmacy. Thin-layer chromatography (TLC) was performed on silica gel 60 F-254 plates (Sigma-Aldrich) using a mixture solution of 70% MeOH and 30% aqueous NH₄OAc (NH₄OAc solution is 20% by weight) as the mobile phase. Ion-exchange chromatography was performed under gravity flow using Dowex 50WX2 (H⁺ form, 200-400 mesh) cation exchange resins. All evaporations were performed at reduced pressure (ca. 20 Torr) using a Büchi rotary evaporator.

HPLC was accomplished on two Waters 515 HPLC pumps, a Waters 2487 absorbance UV detector and a Ludlum Model 2200 radioactivity detector, operated by Waters Empower 2 software. The analytical HPLC was performed on a Phenomenex Luna C18 reversed phase column (5 μm, 250×4.6 mm) and monitored using a radiodetector and UV at 254 nm. The flow was 1.0 mL/min, with the mobile phase starting from 99% solvent B (0.1% TFA in water) and 1% solvent C (0.1% TFA in acetonitrile) (0˜1 min) to 70% solvent B (0.1% TFA in water) and 30% solvent C (0.1% TFA in acetonitrile) (1˜30 min). Radio-TLC was performed with MKC18 silica gel 60 Å plates (Whatman, N.J.) with solvent MeOH/20% NaOAc=3:1 as the eluent using a Bioscan AR2000 imaging scanner (Washington, D.C.) and Winscan 2.2 software.

Synthesis of (1,8-Diamine-Sar) Cobalt (III) tri(tetraphenylborate) ([Co(DiAmSar)](BPh₄)₃.H₂O, 2)

Compound 1 Co(DiAmSar)]Cl₅.H₂O (3.2 g, 5.5 mmol) was dissolved in water (20 mL), followed by the addition of 2 eq NaOH solution (11.0 mmol, sufficient to neutralize the protonated primary amino groups). The resulting mixture was stirred for 30 min at room temperature until pH was near to 7˜8. Sodium tetraphenylborate (5.2 g, 16.5 mmol) in 20 mL methanol was added, and then stirred for 1 h. After filtration and drying under reduced pressure, 6.6 g of compound 2 [Co(DiAmSar)](BPh₄)₃.H₂O (85% yield) was obtained as an orange solid. MS: Calcd for C₈₆H₉₆B₃CoN₈O [M+1-2HBPh₄-H₂O]⁺ m/z 691.7, [M+1-3HBPh₄-H₂O]⁺ 371.4, found 692.1, 371.1. ¹H-NMR (DMSO-d6): 7.20-6.79 (m, 45H, aromatic); 3.10-2.80 (m, 12H, NCCH₂N); 2.60-2.15 (m, 12H, NCH₂CH₂N).

Synthesis of (1-amine, 8-(aminomethyl) 4′-methylbenzoate-Sar) Cobalt (III) Pentachloride ([Co(AmBMSar)]Cl₅.5H₂O, 3)

Compound 2 [Co(DiAmSar)](BPh₄)₃.H₂O (7.6 g, 5.7 mmol) was dissolved in anhydrous MeOH (40 mL) and methyl 4-formylbenzoate (1.6 g, 10.0 mmol), followed by addition of 1.7 mL acetic acid and 4 Å molecular sieves. The solution was refluxed 72 h under argon and shielded from visible light. The reaction mixture was cooled to room temperature, and sodium triacetoxyborohydride (NaHB(OAc)₃, 9.7 g, 45.0 mmol) was added. The resulting mixture was stirred overnight. The products were loaded onto silica gel and initially purified by flash column chromatography, using a mixture of 70% MeOH and 30% aqueous NH₄OAc solution as the eluting solvent. The fractions were monitored by silica gel TLC. This initial column chromatography partially separated the biscoupled Co-cage complex and the mono-coupled Co-cage [Co(AmBMSar)] complex from the starting material. Each product was further purified by evaporating the MeOH, diluting the remaining aqueous solution ˜10-fold, and loaded on a Dowex 50-WX2 [H⁺] cation exchange resin column. The [Co(AmBMSar)] complex was eluted from the column with 3.0-4.0 M HCl. The HCl eluant was evaporated under reduced pressure to give a yellow solid compound 3 [Co(AmBMSar)]Cl₅.5H₂O (1.8 g, 39.1% yield). MS: Calcd for C₂₃H₅₄Cl₅CoN₈O₇ [M+Na-2HCl-5H₂O]⁺ m/z 650.2, [M-5HCl-5H₂O+Na]⁺ 541.2, found 649.7, 541.2. ¹H-NMR (D₂O): 7.93-7.86 (m, 2H, aromatic); 7.42-7.35 (m, 2H, aromatic); 4.05 (s, 3H, CCH₃); 3.75 (s, 2H, NCH₂C); 3.45-3.26 (m, 12H, NCCH₂N); 2.88-2.75 (m, 12H, NCH₂CH₂N).

Synthesis of (1-amine, 8-(aminomethyl) 4′-carboxybenzene-Sar) Cobalt (III) Trichloride ([Co(AmBaSar)]Cl₃.5H₂O, 4)

Compound 3 [Co(AmSarBM)]Cl₅.5H₂O (2.4 g, 3.0 mmol) was dissolved in the solution of methanol (40 mL)/water (30 mL) containing potassium carbonate (3.0 g), and refluxed for 5 h. The reaction mixture was then neutralized with hydrochloric acid, diluted to 1 L, sorbed on Dowex 50-WX2 [H⁺] cation exchange resin column, and eluted with hydrochloric acid (2˜3 M, 2 L). The dark red fraction was collected and evaporated to dryness. 1.8 g compound 4 was obtained in 89% yield. MS: Calcd for C₂₂H₅₀Cl₃CoN₈O₇ [M+Na]+m/z 724.2, [M+Na-5H₂O]⁺ 634.2, found 724.1, 634.3. ¹H-NMR (D₂O): 7.91-7.87 (m, 2H, aromatic); 7.42-7.36 (m, 2H, aromatic); 4.00 (s, 2H, NCH₂C); 3.47-3.27 (m, 12H, NCCH₂N); 3.07-2.73 (m, 12H, NCH₂CH₂N).

Synthesis of. Methyl 4-((8-amino-3, 6, 10, 13, 16, 19-hexaazabicyclo [6.6.6] icosane-1-ylamino) methyl) benzoate (AmMBSar, 5)

Compound 3 [Co(AmBMSar)]Cl₅.5H₂O (790 mg, 1.0 mmol), NaOH (95 mg, sufficient to neutralize the protonated primary amino groups) and CoC1₂.6H₂O (260 mg) were dissolved in deoxygenated water (20 mL) under nitrogen. The solution turned green from brown after NaCN (1.0 g) was added. The resulting mixture continued to react in 70° C. under nitrogen until the solution had become almost colourless (overnight). This final solution was evaporated under reduced pressure, and the residue was extracted with boiling acetonitrile (3×15 mL). The total extract was filtered, and dried under vacuum to provided compound 5 AmMBSar (110 mg, 24.5% yield).

Synthesis of AmBaSar (6)

AmBaSar was prepared by two methods:

Method 1.

This is similar to the preparation of AmMBSar from compound 3. Briefly, the cobalt ion on compound 4 was removed to produce the target compound 6 AmBaSar (26% yield) by reduction with excess cyanide ion to yield the free cage.

Method 2.

Compound 5 was alkaline hydrolyzed to produce the target compound 6 AmBaSar (80.2%, yield).

Radiolabeling of BFC AmBaSar and DOTA, Evaluation of Radiolabeled AmBaSar and Comparison with Radiolabeled DOTA.

FIG. 9 shows a method for the ⁶⁴Cu radiolabeling of AmBaSar according to the present invention. AmBaSar (2.5˜25 μg) was labeled with ⁶⁴Cu (1˜5 mCi) in 0.1 M ammonium acetate solution (pH 5.0) at room temperature (23˜25° C.) for 5 min to 30 min. After 5 min complexation, the radiolabeling yield of ⁶⁴Cu-AmBaSar was more than 97%. The AmBaSar was nearly quantitatively labeled with ⁶⁴Cu²⁺ within 30 min under the above experimental conditions. The complexation rates by the AmBaSar at pH 5 with ⁶⁴Cu²⁺ was satisfactory for its use in the development of ⁶⁴Cu-radiopharmaceuticals. In conclusion, the new functionalized AmBaSar can efficiently label ⁶⁴Cu²⁺ at room temperature due to the provision of a three-dimensional hexa-aza cage by increasing thermodynamic and kinetic stability to the ⁶⁴Cu²⁺ complex, which is similar with other Sar based ligands.

The radiochemical yield of ⁶⁴Cu-AmBaSar was determined by radio-HPLC or radio-TLC after different time points. In HPLC, the free ⁶⁴Cu was eluted at about 3.6 min, while the retention time of ⁶⁴Cu-AmBaSar was 17.9 min. A typical HPLC of crude ⁶⁴Cu-AmBaSar is shown in FIG. 10. For TLC, the R_(f) value of free ⁶⁴Cu and complexed ⁶⁴Cu-AmBaSar were well-separated. ⁶⁴Cu remained at the origin (R_(f)=0) and the ⁶⁴Cu-AmBaSar complex close to solvent front (R_(f)=0.71). The radiochemical yield of ⁶⁴Cu-AmBaSar was determined to be more than 98%.

⁶⁴Cu-DOTA was prepared following literature procedures. (Refs. 25, 26) The radiochemical yield of ⁶⁴Cu-DOTA was determined by radio-TLC after different time points. The radiochemical yield of ⁶⁴Cu-DOTA was more than 98% after the complexation.

Lipophilicity (Octanol/Water Partition Coefficient) Studies.

Information about the lipophilicity of the ⁶⁴Cu-AmBaSar and ⁶⁴Cu-DOTA was obtained by measuring their partitioning in a 1-octanol/water system. Counts in samples were used to determine partition coefficients (log P) values, calculated using a known formula. The log P values were measured at pH 7.4 in PBS. The log P value of ⁶⁴Cu-AmBaSar is −2.6, and the corresponding value of ⁶⁴Cu-DOTA is −2.3. Both ⁶⁴Cu-AmBaSar and ⁶⁴Cu-DOTA are hydrophilic. This indicates that they should be predestined to show rapid blood clearance and preferential renal excretion.

In Vitro Studies.

The stability of the BFC copper-64 complex under physiological conditions is very important. In vitro stability of ⁶⁴Cu-AmBaSar in PBS (pH 7.4) and FBS solutions at physiological temperatures was tested and the results are shown in FIG. 11. In vitro stability of ⁶⁴Cu-AmBaSar was determined in the PBS or FBS using HPLC or TLC after incubating for different time intervals (2, 4, 20, and 26 h). The radiochemical purity of ⁶⁴Cu-AmBaSar in the PBS or FBS is more than 97% after 26 hours incubation. The stability of ⁶⁴Cu-AmBaSar in mouse blood was also. Over 98% of ⁶⁴Cu-AmBaSar remained untouched after its incubation for 4 h. These in vitro stability studies demonstrated that the ⁶⁴Cu-AmBaSar is very stable in PBS, FBS, and the blood at physiological pH.

In Vivo Studies.

MicroPET imaging and biodistribution studies were performed with the non-targeted ⁶⁴Cu-AmBaSar and ⁶⁴Cu-DOTA complexes to allow a comparison of their base-line organ uptake and clearance properties. The micro-PET imaging results were shown in FIG. 12. After 30 min, the radioactivity quickly cleared from muscle and blood, and mainly localized in the bladder and kidneys. Regarding ⁶⁴Cu-DOTA, the radioactivity mainly localized in the bladder, kidneys, and liver. At the 30 min time point, both ⁶⁴Cu-DOTA and ⁶⁴Cu-AmBaSar showed high kidney uptake, with ⁶⁴Cu-DOTA having a much higher liver uptake than ⁶⁴Cu-AmBaSar. By two hours renal activity cleared significantly for both agents, although liver and bowel activity remained in the animals receiving ⁶⁴Cu-DOTA. Although more detailed pharmacokinetic analyses are required, renal activity for ⁶⁴Cu-AmBaSar decreased by 51% between 30 min and 2 hours based on the micro-PET region of interest quantification, comparing favorably with ⁶⁴Cu-DOTA clearance (66%).

The biodistribution of ⁶⁴Cu-AmBaSar and ⁶⁴Cu-DOTA were assessed in Balb/c mice. Each animal was sacrificed at the time interval 2 h and the organs dissected. The values of percent injected dose/gram (ID/g %) in different organs were compared and illustrated in FIG. 13. The ⁶⁴Cu-AmBaSar cleared rapidly from the blood and predominantly through the kidneys. After 2 h, the kidney and liver uptake reached 1.09±0.27, 0.14±0.01% ID/g, respectively, which is consistent with the excretion pattern from the microPET imaging results. The ⁶⁴Cu-DOTA cleared through the kidney and liver, with uptake reached 1.28±0.41, 1.25±0.09, respectively, by 2 h.

Copper ion in vivo is responsible for many enzymatic processes and hence can be bound by many proteins. Its natural excretory path is via the hepatocytes in the liver. It may be recirculated by binding to ceruloplasmin in the liver. While rapid clearance through the kidneys is typical of charged ⁶⁴Cu-complexes which maintain their identity, hepatobiliary clearance of ⁶⁴Cu-radiopharmaceuticals is much less desirable, and its presence usually suggests loss of Cu-64 from the ligand. (1, 28) Prasanphanich A F, Retzloff L, Lane S R, Nanda P K, Sieckman G L, Rold T L, et al. In vitro and in vivo analysis of [⁶⁴Cu-NO2A-8-Aoc-BBN(7-14)NH₂]: a site-directed radiopharmaceutical for positron-emission tomography imaging of T-47D human breast cancer tumors. Nucl Med Biol 2009; 36:171-81. Rapid renal clearance, as opposed to mixed renal and hepatic clearance resulting from administration of ⁶⁴Cu-DOTA, will provide better somatic contrast from the imaging perspective, and potentially reduce radiation exposure for therapeutic analogues. Therefore, the development of more stable chelators would be beneficial as free Cu clears through liver. The hydrophilicity of ⁶⁴Cu-AmBaSar (log P=−2.6) is only slightly different from ⁶⁴Cu-DOTA (log P=−2.3). Both compounds should mainly clear through the kidneys. For ⁶⁴Cu-AmBaSar, residual kidney uptake and low liver accumulation at 2 h post injection were observed in both the microPET images and biodistribution studies, compared with high residual liver and bowel accumulation with ⁶⁴Cu-DOTA. However, with similar hydrophilicity, the liver uptake of ⁶⁴Cu-DOTA is eight times higher than that of ⁶⁴Cu-AmBaSar. The comparative data from microPET imaging and biodistribution studies between ⁶⁴Cu-AmBaSar and ⁶⁴Cu-DOTA supports the assumption that ⁶⁴Cu-AmBaSar is more stable in vivo than ⁶⁴Cu-DOTA. Nonetheless, the differential organ uptake and clearance properties could also be partially attributed to the characteristics of the BFC AmBaSar with polyamine functional groups, and DOTA with polyacid functional groups. Although accumulation of radioactivity in liver is likely related to the loss ⁶⁴Cu from the DOTA chelator, further biochemical testing may be required to determine the disposition of ⁶⁴Cu in liver.

Materials and Methods

Bifunctional Chelator AmBaSar Labeling Copper-64.

[⁶⁴Cu]Acetate (⁶⁴Cu(OAc)₂) was prepared by adding 185 MBq (5 mCi) of ⁶⁴CuCl₂ in 0.1 M HCl into an 1.5 mL microfuge tube containing 300 μL 0.1 M ammonium acetate (pH 5.0). The mixture was vortexed and incubated for 15 min at room temperature. AmBaSar (2.5-25 μg), diluted in 100 μL of 0.1 M ammonium acetate (pH 5.0), was mixed with 1˜5 mCi of ⁶⁴Cu(OAc)₂. The solution was then incubated at room temperature (23˜25° C.) for 5 min˜30 min. The radiochemical yield was determined by radio-HPLC or radio-TLC at different time points. ⁶⁴Cu-AmBaSar was purified by radio-HPLC, and the eluant was evaporated and reconstituted in saline, which was filtered into a sterile dose vial for use in animal experiments by passage through a 0.22 μm Millipore filter.

Bifunctional Chelator DOTA Labeling Copper-64.

DOTA (20 μg) was labeled with ⁶⁴Cu²⁺ by addition of 2 mCi of ⁶⁴Cu²⁺ in 0.1 M sodium acetate buffer (pH 5.5) followed by 45 min incubation at 45° C. The radiochemical yield was determined by radio-TLC (the same condition with ⁶⁴Cu-AmBaSar).

Determination of the Partition Coefficient Log P.

The partition coefficient value was expressed as log P. Log P of ⁶⁴Cu-AmBaSar or ⁶⁴Cu-DOTA was determined by measuring the distribution of radioactivity in 1-octanol and PBS. A 5 μL sample of ⁶⁴Cu-AmBaSar or ⁶⁴Cu-DOTA in PBS was added to a vial containing 1 mL each of 1-octanol and PBS. After vortexing for 5 min, the vial was centrifuged for 5 min to ensure complete separation of layers. Then, 5 μL of each layer was pipetted into other test tubes and radioactivity was measured using a gamma counter (Packard). The measurement was repeated three times.

In Vitro Stability Assessment.

The stability of the ⁶⁴Cu-AmBaSar was assayed by measuring the radiochemical purity after different incubation times at room temperature or 37° C. For the in vitro stability study, 100 μCi of the ⁶⁴Cu-AmBaSar was pipetted into 1 mL of PBS and fetal bovine serum (FBS), respectively, followed by incubation in PBS at room temperature and in FBS at 37° C. An aliquot of the mixture was removed for the determination of radiochemical purity by HPLC at different time points after incubation (2, 4, 20, and 26 h). The solution of FBS was centrifugated, and the upper solution was taken and filtered for HPLC analysis.

MicroPET Imaging and Biodistribution.

MicroPET imaging and biodistribution of the radiolabeled BFCs were performed on Balb/c mice to evaluate their in vivo properties. Animals (Balb/c, n=2) were injected with 0.3 mCi ⁶⁴Cu-AmBaSar or ⁶⁴Cu-DOTA through the tail vein. PET imaging (10-min static scans) was performed using a microPET R4 scanner (Concorde Microsystems, Inc, Knoxville, Tenn.), with 120 transaxial planes and spatial resolution of 1.2 mm, at 30 min and 2 h postinjection. The microPET data were reconstructed using the ordered subsets expectation maximization (OSEM) algorithm using the microPET Manager Software (CTI Concorde Microsystems, Inc, Knoxville, Tenn.). Images were then analyzed using the Acquisition Sinogram Image Processing (ASIPro) software (CTI Concorde Microsystems, Inc, Knoxville, Tenn.).

For biodistribution studies, one group of mice (Balb/c, n=3) was injected intravenously with the radiotracer ⁶⁴Cu-AmBaSar (10 μCi, 100 μL). Another group of mice was injected similarly with ⁶⁴Cu-DOTA (10 μCi, 100 μL). Activity injected into each mouse was measured in a dose calibrator (Capintec). After inhalation anesthesia, animals were sacrificed at 2 h postinjection. Tissues and organs of interest were separated and weighed. Radioactivity in each organ was measured using a gamma counter, and radioactivity uptake was expressed as % ID/g. Mean uptake (% ID/g) for each group of animals was calculated with standard deviations.

Copper-64 Labeled AmBaSar Conjugated Cyclic RGD Peptide for Improved MicroPET Imaging of Integrin α_(v)β₃ Expression

⁶⁴Cu-AmBaSar-RGD was obtained in high yield under mild conditions for PET imaging of integrin α_(v)β₃ expression. This tracer exhibits good tumor-targeting efficacy, excellent metabolic stability, as well as favorable in vivo pharmacokinetics. In vitro and in vivo evaluation of the ⁶⁴Cu-AmBaSar-RGD shows it has improved in vivo stability compared with the established tracer ⁶⁴Cu-DOTA-RGD. The AmBaSar chelator has general application for ⁶⁴Cu labeling of various bioactive molecules in high radiochemical yield and high in vivo stability for future PET applications.

Syntheses of AmBaSar-RGD and DOTA-RGD

AmBaSar could be activated and conjugated to the cyclic RGDyk peptide in a water-soluble procedure as described herein. The conjugation can also be performed in organic phase according to literature procedures (Refs. 29, 30) In brief: the solution of AmBaSar (4.5 mg, 0.01 mmol), HATU (3.8 mg, 0.01 mmol), HOAt (1.4 mg, 0.01 mmol), and dimethyl sulfoxide (DMSO, 0.5 mL) were stirred at room temperature for 10 min. Seven equivalent of DIPEA (9.1 mg, 0.07 mmol) and cyclic RGDyk (1.2 mg, 0.002 mmol) in 300 μL DMSO were then added to the mixture at 0° C. The mixture was stirred for 3 h at room temperature, and the solvent removed in vacuo. The residue was dissolved in acetonitrile/water (1:3) containing 0.1% TFA and purified by semipreparative HPLC. AmBaSar-RGD was obtained as a white solid material after lyophilization. DOTA was activated and conjugated to cyclic RGDyk according to literature methods. (Ref. 31)

DOTA-RGD was also purified by semipreparative HPLC and confirmed by mass spectrometry. AmBaSar-RGD and DOTA-RGD conjugates were dissolved in 0.1 N ammonium acetate buffer solution (pH 5˜5.5), respectively, and stored in −20° C. for the future use in radiolabeling reactions.

Copper-64 Labeling and Formulation.

The ⁶⁴Cu-AmBaSar-RGD was prepared as described supra with minor modifications as follows: [⁶⁴Cu]Acetate (⁶⁴Cu(OAc)₂) was prepared by adding 37-111 MBq of ⁶⁴CuCl₂ in 0.1 N HCl into 300 μL 0.1 N ammonium acetate buffer (pH 5.0˜5.5), followed by mixing and incubating for 15 min at room temperature. The AmBaSar-RGD (about 2˜5 μg in 100 μL 0.1 N ammonium acetate buffer) was added to the above ⁶⁴Cu(OAc)₂ solution. The resulting mixture was incubated at temperature 23˜37° C. for 30 min. The ⁶⁴Cu-AmBaSar-RGD was determined and purified by semipreparative HPLC. The radioactive peak containing ⁶⁴Cu-AmBaSar-RGD was collected and concentrated by rotary evaporation to remove organic solvent. And the radioactivity was reconstituted in 500-800 μL phosphate buffered saline (PBS), and passed through a 0.22 μm Millipore filter into a sterile dose vial for use in experiments below.

Details of the ⁶⁴Cu-labeling DOTA-RGD procedure were reported earlier. (Ref. 31) In brief, 37˜111 MBq of ⁶⁴CuCl₂ in 0.1N HCl were diluted in 300 μL of 0.1 N ammonium acetate buffer (pH 5.5), and added to the DOTA-RGD solution (about 2˜5 μg in the 100 μL 0.1 N ammonium acetate buffer). The reaction mixture was incubated at 45° C. for 45 min. The radiochemical yield was determined by radio-TLC and HPLC. ⁶⁴Cu-DOTA-RGD was then purified by semipreparative HPLC, and the radioactive peak containing the desired product was collected. After removal of the solvent by rotary evaporation, the residue was reconstituted in 500-800 μL of PBS and passed through 0.22 μm Millipore filter into a sterile multidose vial for use in following experiments.

Determination of Log P Value.

The partition coefficient value was expressed as log P. Log P of ⁶⁴Cu-AmBaSar-RGD was determined by measuring the distribution of radioactivity in 1-octanol and PBS. A 5 μL sample of ⁶⁴Cu-AmBaSar-RGD in PBS was added to a vial containing 1 mL each of 1-octanol and PBS. After vigorously vortexing for 10 min, the vial was centrifuged for 5 min to ensure the complete separation of layers. Then, 3×10 μL of each layer was pipetted into other test tubes and radioactivity was measured using a gamma counter (Perkin-Elmer Packard Cobra). The measurement was repeated three times, and Log P values were calculated according to a known formula.

In Vitro Stability Assay.

The in vitro stability of the ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD were studied at different time points. In brief, 3.7 MBq of the ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD were pipetted into 1 mL of the PBS, fetal bovine serum (FBS), and mouse serum, respectively. After incubated at 37° C. for 3, 18, and 24 h, an aliquot of the mixture was removed from the PBS solution and the radiochemical purity was determined with HPLC. For the solution of FBS and mouse serum, the aliquots were added to 100 μL PBS with 50% TFA. After centrifugation, the upper solution was taken and filtered for HPLC analysis.

Cell Uptake Study.

U87MG human glioblastoma cell line (integrin α_(v)β₃-positive) was obtained from the American Type Culture Collection (ATCC, Manassas, Va.) and maintained under standard conditions according to ATCC as following: The U87MG glioma cells were grown in Gibco's Dulbecco's medium supplemented with 10% fetal bovine serum (FBS), 100 IU/mL penicillin, and 100 μg/mL streptomycin (Invitrogen Co, Carlsbad, Calif.), at 37° C. in humidified atmosphere containing 5% CO₂. The U87MG glioma cells were grown in culture until sufficient cells were available.

The cell uptake study was performed as described in the literature with some modifications. (Ref. 30) Cells were incubated with ⁶⁴Cu-AmBaSar-RGD (37 kBq/well) or ⁶⁴Cu-DOTA-RGD at 37° C. for 30 min, 60 min, and 120 min. The blocking experiment was performed by incubating U87MG cells with ⁶⁴Cu-AmBaSar-RGD (37 kBq/well) in the presence of 2 μg RGD. The tumor cells were then washed three times with chilled PBS and harvested by 0.1 N NaOH solution containing 0.5% sodium dodecyl sulfate (SDS). The cell suspensions were collected and measured in the gamma counter.

Animal Model.

Athymic nude mice (about 10-20 weeks old, with a body weight of 25-35 g) were obtained from Harlan (Charles River, Mass.). All animal experiments were performed according to a protocol approved by University of Southern California Institutional Animal Care and Use Committee. The U87MG human glioma xenograft model was generated by subcutaneous injection of 5×10⁶ U87MG human glioma cells into the front flank of athymic nude mice. The tumors were allowed to grow 3-5 weeks until 200-500 mm³ in volume. Tumor growth was followed by caliper measurements of the perpendicular dimensions.

MicroPET Imaging and Blocking Experiment.

MicroPET scans and imaging analysis were performed using a rodent scanner (microPET R4; Siemens Medical Solutions) as previously reported (26). [26] Li, Z., Cai, W., Cao, Q., Chen, K., Wu, Z., He, L., and Chen, X. (2007) ⁶⁴Cu-labeled tetrameric and octameric RGD peptides for small-animal PET of tumor α_(v)β₃ integrin expression. J Nucl Med 48, 1162-71. About 11.1 MBq of ⁶⁴Cu-AmBaSar-RGD or ⁶⁴Cu-DOTA-RGD was intravenously injected into each mouse under isoflurane anesthesia. Ten minute static scans were acquired at 1, 2, 4, and 20 h post injection. The images were reconstructed by a 2-dimensional ordered-subsets expectation maximum (OSEM) algorithm. For each microPET scan, regions of interest were drawn over the tumor, normal tissue, and major organs on the decay-corrected whole-body coronal images. The radioactivity concentration (accumulation) within the tumor, muscle, liver, and kidneys were obtained from the mean value within the multiple regions of interest and then converted to % ID/g. For the receptor blocking experiment, mice bearing U87MG tumors were scanned (10 min static) at 2 h time point after the coinjection of 11.1 MBq of ⁶⁴Cu-AmBaSar-RGD or ⁶⁴Cu-DOTA-RGD with 10 mg/kg c(RGDyK) per mouse.

Biodistribution Studies.

The U87MG tumor bearing nude mice (n=3) were injected with 0.37 MBq of ⁶⁴Cu-AmBaSar-RGD or ⁶⁴Cu-DOTA-RGD to evaluate the biodistribution of these tracers. All mice were sacrificed and dissected at 20 h after the injection of the tracers. Blood, U87MG tumor, major organs, and tissues were collected and weighed wet. The radioactivity in the tissues was measured using the gamma counter. The results were presented as percentage injected dose per gram of tissue (% ID/g). For each mouse, the radioactivity of the tissue samples was calibrated against a known aliquot of the injected activity. Mean uptake (% ID/g) for each group of animals was calculated with standard deviations.

Metabolic Stability.

The metabolic stabilities of ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD were evaluated in an athymic nude mouse bearing a U87MG tumor. Sixty minutes after intravenous injection of 11.1 MBq of ⁶⁴Cu-AmBaSar-RGD or ⁶⁴Cu-DOTA-RGD, the mouse was sacrificed and relevant organs were harvested. The blood was collected and immediately centrifuged for 5 min at 13,200 rpm, and the upper serum solution was added to 100 μL PBS solution containing 50% TFA, followed by mixing and centrifugation for 10 min, and the upper solution was then taken out and filtered for HPLC analysis. Liver, kidneys, and tumor were homogenized using a homogenizer, suspended in 1 mL of PBS buffer, and centrifuged for 10 min at 14,000 rpm, respectively. For each sample, after removal of the supernatant, the solution was added to 100 μL PBS solution containing 50% TFA, followed by mixing and centrifugation for 10 min, and the upper solution was then taken and filtered for HPLC analysis. Radioactivity was monitored using a solid-state radiation detector. The eluent was also collected using a fraction collector (1.5 min/fraction) and the radioactivity of each fraction was measured with the γ counter.

Statistical Analysis.

Quantitative data were expressed as mean±SD. Means were compared using One-way ANOVA and student's t-test. P values <0.05 were considered statistically significant.

Results

Chemistry and Radiolabeling.

The AmBaSar-RGD conjugate was obtained in about 80% yield after HPLC purification for both aqueous and organic phase procedures. The ⁶⁴Cu-labeling (n=7) was achieved in more than 95% decay-corrected yield for ⁶⁴Cu-AmBaSar-RGD with radiochemical purity of >99%, and 80% radiochemical yield for ⁶⁴Cu-DOTA-RGD with radiochemical purity >98%. ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD were analyzed and purified by HPLC. The HPLC retention times of ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD was 26.5 min and 21.5 min, respectively, under the analytical condition. For radio-TLC analysis, the free ⁶⁴Cu²⁺ remained at the origin of TLC plate, while the R_(f) values of ⁶⁴Cu-DOTA-RGD and ⁶⁴Cu-AmBaSar-RGD were about 0.8˜1.0. The specific activity of ⁶⁴Cu-DOTA-RGD and ⁶⁴Cu-AmBaSar-RGD was estimated to be about 10.1-22.2 GBq/μmol. Both tracers were used immediately after the formulation.

Log P Value and In Vitro Stability.

The octanol/water partition coefficients (log P) for ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD were −2.44±0.12 and −2.80±0.04, respectively (Ref. 31), which demonstrated that both tracers are rather hydrophilic. The in vitro stability of ⁶⁴Cu-AmBaSar-RGD was also studied in PBS (pH 7.4), FBS, and mouse serum for different time intervals (3, 18, and 24 h) at physiological temperature 37° C. The stability was presented as percentage of intact ⁶⁴Cu-AmBaSar-RGD based on the HPLC analysis and the results are shown in FIG. 15. After 24 h incubation, more than 97% of ⁶⁴Cu-AmBaSar-RGD remained intact in the PBS and FBS, and more than 95% of ⁶⁴Cu-AmBaSar-RGD remained intact in mouse serum. We also found that ⁶⁴Cu-DOTA-RGD demonstrated similar stability results in vitro under the above experimental conditions (data not shown).

In Vitro Cell Uptake.

Cell uptake study of ⁶⁴Cu-AmBaSar-RGD or ⁶⁴Cu-DOTA-RGD was performed on U87MG tumor cells, and the cell uptake was expressed as radioactivity (cpm) per 10⁶ cells after decay correction as shown in FIG. 16. The cell uptake study revealed that both ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD could bind to U87MG tumor cells, but relatively low amounts of activity (only about 0.1˜0.4% was internalized). However, this binding could be efficiently blocked by excess amount of cold cyclic RGD peptide, which demonstrated the binding specificity of the radiolabeled ligands.

MicroPET Imaging.

The tumor-targeting efficacy and biodistribution patterns of ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD were evaluated in nude mice bearing U87MG human glioma xenograft tumors (n=3) at multiple time points (1, 2, 4, and 20 h) with static microPET scans. Representative decay-corrected coronal images at different time points were shown in FIG. 17A. The U87MG tumors were clearly visualized with high tumor-to-background contrast for both tracers. The uptake of ⁶⁴Cu-AmBaSar-RGD in U87MG tumors was 2.04±0.14, 1.85±0.16, 1.87±0.11, and 0.97±0.05% ID/g at 1, 2, 4, and 20 h p.i., respectively. ⁶⁴Cu-DOTA-RGD demonstrated similar tumor uptake with the value of 2.03±0.10, 1.97±0.05, 1.88±0.29, and 0.88±0.07% ID/g at the above time points, respectively (FIG. 4B-3). However, the biodistribution patterns of ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD were significantly different, especially in the kidneys and liver. The renal uptake of ⁶⁴Cu-AmBaSar-RGD were 2.83±0.77, 2.68±0.55, 2.49±0.50, and 1.43±0.35% ID/g at 1, 2, 4, and 20 h p.i., respectively; while the corresponding uptake for ⁶⁴Cu-DOTA-RGD was 1.52±0.46, 1.33±0.23, 1.55±0.61, and 1.58±0.13% ID/g, respectively. This was lower than that of ⁶⁴Cu-AmBaSar-RGD from 1 to 4 h, and reached comparable levels at 20 h time point. The liver uptake for ⁶⁴Cu-AmBaSar-RGD was 0.89±0.13, 0.76±0.13, 0.75±0.14, and 0.64±0.06% ID/g at 1, 2, 4, and 20 h p.i. The corresponding uptake value for ⁶⁴Cu-DOTA-RGD was 2.28±1.08, 2.31±1.34, 2.15±0.90, and 2.52±1.43% ID/g respectively, which were significantly higher than those of ⁶⁴Cu-AmBaSar-RGD at all time points.

Blocking Experiment.

The integrin α_(v)β₃ receptor specificity of ⁶⁴Cu-AmBaSar-RGD was confirmed by a blocking experiment where the tracers were co-injected with c(RGDyK) (10 mg/kg). As can be seen from FIG. 18, the U87MG tumor uptake in the presence of non-radiolabeled RGD peptide (0.09±0.03% ID/g) is significantly lower than that without RGD blocking (1.85±0.16% ID/g) (P<0.05) at 2 h p.i. The uptake of ⁶⁴Cu-AmBaSar-RGD in other organs (heart, intestine, kidneys, lungs, liver, and spleen) was also significantly decreased, which correlates well with previous references. (Ref. 31) Similarly, the integrin α_(v)β₃ specificity of ⁶⁴Cu-DOTA-RGD was confirmed by blocking experiments (FIG. 18).

Biodistribution Studies.

To validate the accuracy of small animal PET quantification, we also performed a biodistribution experiment by using the direct tissue sampling technique. The data shown as the percentage administered activity (injected dose) per gram of tissue (% ID/g) in FIG. 19A. Both ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD mainly accumulated in kidneys, liver, stomach, intestine, and tumor. After 20 h p.i., the kidneys and liver uptake reached 1.51±0.27 and 0.55±0.06% ID/g for ⁶⁴Cu-AmBaSar-RGD, and 0.98±0.40 and 2.16±0.85% ID/g for ⁶⁴Cu-DOTA-RGD, respectively. This difference was consistent with the excretion pattern from the microPET imaging results. Based on the biodistribution results, we also calculated the contrast of tumor to main organs, which is shown in FIG. 19B. For ⁶⁴Cu-AmBaSar-RGD, the ratio of tumor uptake to muscle, heart, lung, liver, and kidney uptake was 14.20±3.84, 7.33±1.55, 3.34±0.70, 1.18±0.05, and 0.43±0.06, respectively; while the corresponding value for ⁶⁴Cu-DOTA-RGD were 5.97±2.25, 1.78±0.37, 1.27±0.37, 0.33±0.09, and 0.66±0.04, respectively.

Metabolic Stability of ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD.

The metabolic stability of ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD were determined in mouse blood and in liver, kidney and tumor homogenates at 1 h after intravenous injection of radiotracer into a U87MG tumor-bearing mouse according to the literature procedures. (Refs. 32, 33). The radioactivity of each sample was analyzed by HPLC and the representative radio-HPLC profiles were shown in FIG. 20A and FIG. 20B. The retention time of free ⁶⁴Cu²⁺ was around. 3.0 min and the ⁶⁴Cu-AmBaSar-RGD complex was around 15˜16 min (FIG. 20A). The amount of intact tracer in the blood, tumor, liver, and kidneys were approximately 88%, 95%, 98%, and 98% for ⁶⁴Cu-AmBaSar-RGD (FIG. 20A) and 38%, 87%, 34%, and 74% for ⁶⁴Cu-DOTA-RGD (FIG. 20B) at 1 h post injection, respectively.

These experiments demonstrated the ⁶⁴Cu-complexing moiety, AmBaSar is a superior ligand for an imaging application and targeted radiotherapy due to its improved stability compared with DOTA. The new PET tracer ⁶⁴Cu-AmBaSar-RGD can be used for imaging integrin α_(v)β₃ expression. Our studies demonstrate that ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD have comparable in vitro stability, lipophilicity, and tumor uptake. However, ⁶⁴Cu-AmBaSar-RGD did demonstrate improved in vivo stability and biodistribution pattern compared with ⁶⁴Cu-DOTA-RGD.

For radiochemistry, the ⁶⁴Cu²⁺ labeling condition of AmBaSar-RGD was more favorable and the ⁶⁴Cu-AmBaSar-RGD could be obtained with higher radiochemical yield (≧95%) and purity (≧99%) under mild conditions (pH 5.0˜5.5, 23˜37° C.) in less than 30 min, compared with 90% radiochemical yield for ⁶⁴Cu-DOTA-RGD after incubation at 45° C. for 45 min.

Under in vitro conditions, both ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD were very stable in PBS, FBS, and mouse serum solutions at physiological temperature. The Log P is a very useful parameter that can be used to understand the behavior of drug molecules and predict the distribution of a drug compound in a biological system in combination with the other parameters. (Ref. 34). The log P values of ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD indicated that both tracers are rather hydrophilic and they should show rapid blood clearance and preferential renal excretion if they are stable in vivo. However, compared with ⁶⁴Cu-AmBaSar-RGD, ⁶⁴Cu-DOTA-RGD had significantly higher liver uptake (˜2-3 times) based on microPET imaging and biodistribution studies, which indicated that ⁶⁴Cu-DOTA-RGD is less stable than ⁶⁴Cu-AmBaSar-RGD in vivo. In microPET studies, the U87MG tumor uptake of ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD were comparable at selected time points, and the binding specificity was proven by the blocking experiment. The biodistribution study was consistent with the microPET studies. Similar tumor uptake of both tracers may be attributed to their comparable hydrophilicity and the minimal impact of chelators on the integrin binding affinity of RGD peptides. (Ref. 35) ⁶⁴Cu-AmBaSar-RGD cleared rapidly from the blood and predominantly through the kidneys and ⁶⁴Cu-DOTA-RGD mainly cleared through both kidneys and liver. This difference might because that ⁶⁴Cu-AmBaSar-RGD is more stable in vivo compared with ⁶⁴Cu-DOTA-RGD, which would result in reduced nonspecific binding. To further confirm this statement, we also studied the metabolic stability of ⁶⁴Cu-AmBaSar-RGD and ⁶⁴Cu-DOTA-RGD in blood, liver, kidneys, and tumor in nude mice bearing U87MG glioma xenografts after 1 h p.i. injection. Our study clearly demonstrated that the amount of intact ⁶⁴Cu-AmBaSar-RGD was much higher than that of ⁶⁴Cu-DOTA-RGD in blood, tumor, liver, and kidneys. To the best of our knowledge, this is the first study that directly demonstrates that Sar-type chelator, such as AmBaSar, forms more a stable Cu complex in vivo than the established chelator DOTA through direct comparison of their metabolic stability. The rapid renal clearance of ⁶⁴Cu-AmBaSar-RGD, as opposed to the mixed renal and hepatic clearance of ⁶⁴Cu-DOTA-RGD, is preferred as it will provide better somatic contrast from the imaging perspective, and potentially reduce radiation exposure.

Although the invention has been described and explained in terms of specific embodiments and especially embodiments related to the specific BFC AmBaSar, it should be understood that the present invention is not limited to the embodiments specifically discussed and the specific embodiments discussed herein are simply illustrative. As will be appreciated by those skilled in the art, the data and information gleaned from the embodiments discussed with respect to AmBaSar are applicable to the disclosed BFCs not specifically discussed throughout the application.

The following references are incorporated herein by reference in their entirety.

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1-21. (canceled)
 22. A chemical composition comprising a molecule selected from the group consisting of


23. The chemical composition according to claim 22, wherein the molecule is complexed with a metal or metal ion.
 24. The chemical composition according to claim 23, wherein the metal is selected from the group consisting of ⁹⁰Y, Gd, ⁶⁸Ga, ⁵⁷Co, ⁶⁰Co, ⁵²Fe, ⁶⁴Cu and ⁶⁷Cu.
 25. A bifunctional chelator/targeting moiety conjugate comprising a molecule of claim 22, wherein the targeting moiety is selected from the group consisting of a peptide and an antibody.
 26. The bifunctional chelator/targeting moiety conjugate according to claim 25, wherein the peptide is selected from the group consisting of a RGD, Asp-Gly-Glu-Ala (DGEA), bombesin peptides (BBN), uPAR peptides, and other peptides with a lysine amine or N-terminal.
 27. A method of positron emission tomography (PET) imaging comprising: introducing into a subject a chemical composition according to claim
 24. 